Enumeration of CD4+lymphocytes

ABSTRACT

The invention provides a method of enumerating the number of cells of a cell type in a cell sample by (a) counting the white blood cells in the cell sample to obtain the white blood cell population of the sample; (b) determining the proportion or percentage of the cells of the cell type in the white blood cell population in the sample; and (c) calculating the number of cells of the cell type in the sample. The cell type may be a lymphocyte sub-set selected from the group comprising CD4+ lymphocytes, CD45 cells, CD19 cells, CD16 and CD56 positive cells, CD8 cells, CD3 cells or any combination thereof. The method is particularly useful in monitoring the immune status of a patient infected with HIV or other immune deficiency state or disease or condition where CD4+ lymphocytes or CD4+ T cells are monitored or counted.

CROSS-REFERENCE TO RELATED APPLICATIONS

This application is a divisional of U.S. application Ser. No.10/754,711, filed Jan. 12, 2004, pending, which is a continuation ofPCT/IB02/02725 filed on Jul. 11, 2002, which claims priority from SouthAfrica Patent Application No. 2001/5700 filed on Jul. 11, 2001, theentire content of which are hereby incorporated by reference.

BACKGROUND OF THE INVENTION

This invention relates to the enumeration of cells in a cell sample, forexample in a bone marrow cell sample, a body fluid sample, adisaggregated tissue sample, a tissue fine needle aspiration sample or,in particular, a blood sample. More particularly, the invention relatesto a method suitable for, but not limited to, enumerating the number ofCD4+ lymphocytes in a blood sample.

There are several methods for performing cell counting which arecurrently available. The most popular method is flow cytometric celltesting. Non-flow cytometric methods are also available, although thesemethods are less widely used.

Flow Cytometric CD4+ T Cell Testing

Two methods of flow cytometric CD4 testing are utilized worldwide forCD4+ T cell enumeration. The first method involves the use of twomachines and is referred to as the dual or double platform method (DP)(1). This method involves the use of specific panels of antibodiesincluding CD3, CD4, CD8, CD19, CD16, CD56, and CD45. Variousfluorochrome combinations can be used to form either two, three or fourcolor combinations of antibody to constitute the various panels.Duplication of at least one measurement to ensure reproducibility e.g.CD3, is typically performed. In some instances it is recommended thatCD14 expression is also used in the panel to exclude CD14 positivemonocytes from the “lymphocyte” gate and ensure purity of the lymphocytepopulation studied.

The dual platform method makes use of a hematology analyzer to obtain anabsolute lymphocyte count (ALC) [which is obtained by multiplication oftwo independently measured parameters viz. the white cell count and the% lymphocytes of the total white blood cell differential]. A flowcytometer is used to obtain a corresponding CD4 percentage (CD4%) oflymphocytes.

The CD4 antigen expressed on the surface of T cells and monocytes playsan important role in the MHC class II-restricted responses of specific Tlymphocytes. It also serves as the major receptor of humanimmunodeficiency viruses (HIV).

CD45 is a trans-membrane protein tyrosine phosphatase (also calledLeukocyte Common Antigen) that is expressed on all hematopoietic cells.Expression is at a higher density on lymphocytes whilst the expressionis lower on other leukocytes like granulocytes and monocytes. Inaddition to the blood, bone marrow and lymphatics, since CD45 is foundthroughout the hematopoietic lineage, CD45 will be found wherever suchcells constitute a significant portion of the tissue, e.g. spleen,thymus, and bone marrow.

Lymphocytes are defined by flow cytometry either through dual lightscatter parameters, or alternatively (now considered the onlyrecommended method in new guidelines) by the use of dual bright CD45expression with side scatter properties. The lymphocyte population isused as the common denominator or reference point between the hematologyand flow cytometry machines in order to calculate a CD4 T cell of totallymphocytes.

The absolute CD4 count is calculated by multiplying the CD4% (which canalternatively be defined as CD3+/CD4+ T cells) of the total lymphoidpopulation defined by flow cytometry by the ALC, which is then expressedas number of cells per microlitre, or number of cells×106/t, or thenumber of cells×109/t.

Inter-laboratory variation ranging between 15-44% is, however, describedfor the widely used dual platform method (greater than 60% of returns ina recent U. K. NEQAS Immunology shipment have been reported).Theoretically, in order that all laboratories measure lymphocytesequally, the U. K. NEQAS, CDC, NCCLS, and others have devised veryspecific guidelines (1) for use of a “Lymphosum”. The “Lymphosum” itselfis a method of identifying the total lymphoid population by flowcytometry including all T cells (CD3+), all B cells (CD19+) and allNatural Killer cells (CD16+/56+), so that the sum of the individualcomponents equals approximately 100% of lymphocytes.

Various gating strategies that include identification of bright CD45positive cells (lymphocytes) have been recommended to ensure purity ofthe lymphoid population (2) and improve the quality of the assay, butthis is not widely practiced in many countries. The practice ofabbreviated panels, including only CD3/CD4 and CD8 is based loosely oninternational guidelines. It is practiced largely due to costcontainment, and has limited quality control, especially on sampleswhich are older than 6-24 hours, when cell disintegration results inpoor cellular definition and hence problems occur with accurateidentification and subsequent gating of lymphocytes. Use of CD3, CD4 andCD8 antibodies in a single tube to determine the percentage of CD4positive T cells is therefore not recommended for use (1) as there is nomeans in the abbreviated panel of CD3, CD4 and CD8 only to validate thepurity or completeness of the lymphocyte gate.

From the hematology analyzer perspective, white blood cell counts andespecially automated differential counts should ideally be performedwithin 6 hours of venesection and preferably within 24 hours. There iscurrently no known hematology analyzer manufactured that reliablyfacilitates white cell and/or white blood cell differential countingafter 36 hours after blood collection.

Further, different hematology analyzers use different methods ofidentifying lymphocytes and show variation in ALC reporting according tothe specifications of the analyzer, even on fresh samples less than 6hours old. Although the guidelines for identifying lymphocytes by flowcytometry are relatively clear, to date no recommended or universalmethod of identifying lymphocytes or other different types of whiteblood cell on a hematology analyzer exists, despite there being existingknowledge of very specific differential expression of CD45 onlymphocytes. ALC white blood cell differential counts are thereforeneither quality controlled nor standardized between laboratories andresults are therefore unreliable and not directly comparable betweenlaboratories. Because the CD4 count is calculated from the ALC in thedual platform system, it follows that the inaccuracies of the ALC aretranslated to the CD4 count. Thus, the error in each independent step ofeach the separate systems in the dual platform method is multiplied ateach subsequent step in the calculation.

In spite of the relatively wide inter-laboratory variation of CD4 resultreporting, the dual platform flow cytometry system remains the mostwidely used and preferred system for CD4 testing. One of the mainproblems of the dual platform method lies in the identification oflymphocytes as the common denominator or reference point between the twoplatforms. An Absolute Lymphocyte Count (ALC) is a highly variableparameter between laboratories. Currently, although white blood cell(WBC) counts are well quality controlled, both internally on theinstruments themselves and externally on various quality assessmentschemes, white blood cell differential counting methods and techniquesof identifying lymphocytes on various hematology analyzers are neitherquality controlled or standardized. As ALCs are currently used as thecommon denominator and mainstay of dual platform system CD4 counting, ittherefore follows that the documented variability of ALC reporting iscarried over into CD4+ T cell result reporting.

Single Platform Testing

The single platform method (SP) of measuring CD4+ T cells uses flowcytometry only, and both the cell counting and the identification of theCD4+ T cells are performed on the same instrument, a flow cytometer. Itis recommended due to the improved reproducibility of laboratoryresults, the inter-laboratory variation having been reported as varyingbetween 10-18%.

There are several options for performing single platform CD4 testing.One option includes the use of a flow cytometer with a volumetricprecision counting facility, e.g. the Ortho CytoronAbsolute (OrthoDiagnostic Systems, USA) but this instrument is no longer manufactured.The second option utilizes beads as a reference standard from which thecells themselves can be counted. The beads are added to the sample in aknown concentration, either during manufacture or during samplepreparation, in a specified volume, to a similar volume of blood andcounted alongside the cells of interest on a flow cytometer. Bead-basedcounting, although less variable between laboratories, is, however, moretechnically intensive and relies heavily on accurate, precise pipetting,and also on the technical skills of the operator. Duplication of testingis also recommended to assess pipetting error and ensure accuracy ofcounting. This increases further the costs of bead-based testing.

Simplified, smaller single platform flow cytometers dedicated to CD4enumeration (FACSCount, BDS, San Jose; Calif., USA) are also widelyused. Although these instruments are considerably cheaper than flowcytometers, reagents costs for these instruments are more costly thanfor ordinary flow cytometry, thereby also prohibiting their use in manylaboratories.

An additional problem of both the single platform and dual platformsystems is that of the increased costs associated with “Lymphosum”testing. Unfortunately the obviously less expensive “CD4 only”alternatives do not offer sufficient built-in quality control to ensureaccuracy and precision of individual sample testing.

Alternative Technologies for CD4+T Cell Determination

There are also several alternative non-flow cytometric technologies forCD4+ T cell counting available. These include the Dynabead™ assay,Coulter Cytospheres Assay TRAX assay (and Microvolume Fluorimetry TheAbsolute Lymphocyte Count (ALC) has also been proposed as an alternativeto CD4 enumeration where an ALC of less than 1000 cells/μl is used asubstitute for a CD4+ T cell count of 200/μl or less. Poor correlationof these parameters, however, has been shown, and it has been suggestedthat an ALC substitute does not offer meaningful information forindividual patient management.

The current dual methods of CD4 testing are therefore impractical and/orexpensive, and do not provide results which are sufficiently accurate. Aneed thus exists to provide a method which is simple to perform,accommodates existing technologies and is more accurate than currentlymethods employed.

SUMMARY OF THE INVENTION

According to a first embodiment of the invention, there is provided amethod of enumerating the number of cells of a cell type in a cellsample, the method comprising the steps of:

counting the white blood cells in the cell sample to obtain the whiteblood cell population of the sample;

determining the proportion or percentage of the cells of the cell typein the white blood cell population in the sample; and

calculating the number of cells of the cell type in the sample.

The number of cells of the cell type in the sample may be calculated byrelating the proportion or percentage of the cells of the cell type tothe white blood cell population in the sample.

The cell type may be a lymphocyte sub-set, and in particular, alymphocyte sub-set selected from the group comprising CD4+ lymphocytes,CD 45 cells, CD19 cells, CD16 and CD56 positive cells, CD8 cells, CD3cells or any combination thereof. More particularly, the lymphocytesub-set may be CD4+ lymphocytes. The CD4+ lymphocytes may be CD4+ Tcells.

The sample may be whole unlysed blood, unfractionated, fractionated orlysed whole blood. Alternatively, the sample may be whole unlysed bonemarrow, unfractionated, fractionated or lysed whole bone marrow.

Counting the white blood cells (CD45 positive leukocytes) in the samplewill naturally involve identifying the white blood cells in the sample,and any suitable known, conventional or established method may be usedfor such counting (and identification), using any suitable hematologyanalyzer or flow cytometer. For example, identification of nuclearnucleic acid (DNA) staining may be employed as a method of counting thewhite blood cell population (i.e. the white cell count) in the sample.The white blood cell population in the sample may be defined by flowcytometry, either immunophenotypically as CD45+ cells, or, using atechnique substantially similar to DNA staining, as nucleated cells. Thewhite cell population may be counted directly using total CD45expression to obtain a total white cell count, when incorporating beadsas a single platform reference standard in the sample or using avolumetric precision counter.

Actual calculating of the number of CD4+ T cells in the sample may beperformed by multiplying the white blood cell population in the sampleby a factor, which is the proportion of CD4+ T cells in the white bloodcell population when the proportion of CD4+ T cells of the white bloodcell population is expressed as a fraction. If the proportion of CD4+ Tcells in the white blood cell population is expressed as a percentage,then the white blood cell population will be multiplied by a factorwhich is a hundredth of the percentage (%×10⁻²).

The invention thus provides a dual-platform method of establishing (butnot limited to) the number of CD4+ T cells in the sample, using twoseparate parameters.

Counting the white blood cells in the sample may, as indicated above, beby means of a suitable hematology analyzer. Any suitable hematologyanalyzer may be employed, examples being those available under the tradenames GenS™, CELL-DYN™ 4000, and XE2100™, manufactured respectively byBeckman Coulter, Inc. (GenS™), Abbott (CELL-DYN™ 4000) and SysmexCorporation (XE2100™). In turn, determining the proportion of CD4+ Tcells in the white blood cells in the sample may, as indicated above, beby means of a suitable flow cytometer. Any suitable flow cytometer maybe employed, examples being those available under the trade names EPICS™XL and FACSCalibur™, manufactured respectively by Beckman Coulter, Inc.(EPICS™ XL) and BD Biosciences (FACSCalibur™).

While any suitable technique for counting the white blood cells in thesample may be employed, counting said white blood cells may, forexample, be by a size discrimination technique, by an impedancemeasuring technique, or precision volumetric counting.

Similarly, while any suitable technique for determining the proportionof CD4+ T cells in the white blood cells in a sample may be employed,determining the proportion of CD4+ T cells in the white blood cells inthe sample may, for example, be by means of flow-cytometric 90°/sidescatter with CD4 expression. While the counting of the white blood cellsand the determining of the proportion of CD4+ T cells in the sample maybe carried out on separate instruments, namely a hematology analyzer anda flow cytometer, it may be possible to combine the functions of suchinstruments so that both the white blood cell count and thedetermination of the proportion or percentage of CD4+ T cells of thewhite blood cells can conveniently be carried out on a single or commoninstrument.

In a particular embodiment of the invention a dual-platform (i.e.double- or twin-platform) method may be employed, involving two separateinstruments to obtain the CD4+ T cell population (i.e. the absolute CD4+T cell count) in the sample, namely a hematology analyzer to obtain thewhite cell count and a flow cytometer to obtain the fraction orpercentage of CD4+ T cells. The white cell count obtained from thehematology analyzer is then multiplied by the CD4+ T cell fraction orpercentage (as indicated above), measured as a fraction of thepopulation of white blood cells (defined as the CD45+(positive-expressing cells) obtained from the flow cytometer. Thiscalculation facilitates the generation of the absolute CD4+ T cellcount.

Thus, for example, a Beckman Coulter GenS™ hematology analyzer may beused to obtain a white cell count on a blood sample, followed bymeasurement of the CD4+ T cell fraction or percentage of the white bloodcell population (defined by the CD45+ expression thereof) using aBeckman Coulter EPICS™ XL flow cytometer, on the same blood sample.

Instead, a single-platform method may be employed, involving a singleinstrument, the total white cell count and the CD45+ T cell fraction orpercentage of the total white cell population being obtained on a singleinstrument (which may be either a flow cytometer or a hematologyanalyzer). This may be effected by counting the white blood cellsdirectly on a hematology analyzer having a facility for fluorescencemeasurement which can be altered to effect measurement of the fractionor proportion of CD45+ T cells of the total white cell population.Alternatively, the CD45+ T cell fraction or percentage of the totalwhite cell population may be measured directly on a flow cytometer for ablood sample, which flow cytometer has had a suitable (commerciallyavailable) bead counting preparation (such as Beckman CoulterFlow-Count™ Fluorospheres) added thereto, the beads being countedsimultaneously and being used as a standard from which the absolutenumber of CD45+ T cells can be calculated.

The method may additionally comprise one or more of the following steps:

calculating the number of lymphocytes in the sample by relating theproportion or percentage of high density CD45++ bright cells and lowside scatter cells, a component of which is CD4 positive lymphocytes, tothe white blood cell population in the sample, thereby to establish thepopulation of lymphocytes in the sample;

calculating the number of monocytes in the sample by relating theproportion or percentage of moderate density CD45++ cells and mediumside scatter cells, and dim moderate density CD4 cells, to the whiteblood cell population in the sample, thereby to establish the populationof monocytes in the sample; and

calculating the number of granulocytes in the sample by relating theproportion or percentage of dim low density CD45+ cells and CD4 negativecells and high side scatter cells to the white blood cell population inthe sample, thereby to establish the population of granulocytes in thesample.

CD45 and CD4 may be combined either for use with a dual or a singleplatform system to provide at least a three-part (3-part) or at best, afive-part (5-part) white blood cell differential including theidentification of granulocytes, monocytes, lymphocytes, basophils andeosinophils, in addition to the identification of CD4+ lymphocytes (Tcells). Both percentages and absolute counts of each of the individuallatter mentioned cellular compartments can be generated, as describedabove. This may be effected by counting the white blood cellcompartments directly on a hematology analyzer having a facility forfluorescence measurement which can be altered to effect measurement ofthe fraction or proportion of relevant cells of the total white cellpopulation e.g. granulocytes, and the like. Alternatively, theparticular cell fraction or percentage of the total white cellpopulation may be measured directly on a flow cytometer for a bloodsample, which flow cytometer has had a suitable (commercially available)bead counting preparation (such as Beckman Coulter Flow-Count™Fluorospheres) added thereto, the beads being counted simultaneously andbeing used as a standard from which the absolute number of the componentcells e.g. granulocytes and the like can be calculated.

According to a second embodiment of the invention, there is provided akit for use in enumerating the number of CD45+ T cells in a sampleaccording to the method described above, the kit including antibodiesfor use in the method and instructions for performing the method. Thekit may include software for analysis of flow cytometry or hematologyanalyzer data.

The antibodies may be CD4 and/or CD45 antibodies.

The kit may also include computer software for at least partiallyperforming the method of cell enumeration described above.

According to a further embodiment of the invention, there is provided amachine readable medium comprising instructions, which when executed bya machine, cause the machine to perform, at least partially, the methodsteps substantially as described above. The machine readable medium maybe configured for use in conjunction with a flow cytometer and/or ahematology analyzer, and may include instructions for analysis of flowcytometry data.

According to yet a further embodiment of the invention, there isprovided a method of monitoring the immune status of a patient with HIVor other immune deficiency condition or disease, the method includingthe step of enumerating the number of CD45+ lymphocytes or CD45+ T cellsin a cell sample from the patient by a method substantially as describedabove. In particular, the method may be used to determine or monitor thepatient's response to antiretroviral treatment.

BRIEF DESCRIPTION OF THE FIGURES

FIG. 1 shows histograms of dual platform total white blood cell (CD45)assisted CD4 T cell enumeration:

FIG. 1 a shows a histogram of capture of total CD45 positive events (allwhite blood cells) ; and

FIG. 1 b shows a histogram of gated CD45 positive events withidentification of CD4 positive lymphocytes.

FIG. 2 shows histograms of single platform total white blood cell (CD45)assisted CD4 T cell enumeration:

FIG. 2 a shows a histogram of capture of total CD45 positive events (allwhite blood cells), excluding fluorospheres;

FIG. 2 b shows a histogram of gated CD45 positive events withidentification of CD4 positive lymphocytes; and

FIG. 2 c shows a histogram of capture of total CD45 positive events (allwhite blood cells).

FIG. 3 shows histograms of a 5-part white blood cell differential andCD4+ lymphocytes based on use of CD45 and CD4:

FIG. 3 a shows a histogram of capture of total CD45 positive events (allwhite blood cells), including lymphocytes, monocytes, granulocytes andbasophils; and

FIG. 3 b shows a histogram of gated CD45 positive events withidentification of CD4 positive lymphocytes, monocytes, granulocytes andeosinophils.

DETAILED DESCRIPTION OF SOME EMBODIMENTS OF THE INVENTION

The invention will now be described, by way of non-limitingillustration, with reference to the following explanatory examples, withreference to the accompanying drawings.

EXAMPLE 1 Dual-platform Method

A full blood sample was collected from a consenting adult in ethylenediamine tetra-acetic acid (K₃EDTA). This sample was delivered to thelaboratory within 6 hours of venesection. Upon receipt in the laboratorythe sample was subjected to a white blood cell count performed on aBeckman Coulter GenS™ hematology analyzer. A white cell count of4.80×10⁹/l was obtained.

Appropriate external quality assessment and internal quality control asrecommended by the supplier was performed daily on this instrument toensure that the white cell count was accurate and precise.

After the white blood cell count was obtained, blood taken from the samesample was prepared for flow cytometric analysis. Flow cytometricpreparation involved dispensing a well-mixed 100 μl aliquot of wholeblood into the bottom of a 12×75 mm test tube. Anti-CD4 phycoerthryrin(PE) monoclonal antibodies and CD45 Fluorescein-isothiocyanate (FITC)monoclonal antibodies were added (both obtained from Immunotech, BeckmanCoulter, Inc., Miami, Fla.) according to the supplier's recommendationsand incubated for 10 minutes at room temperature, in the dark.

The tube containing the 100 μl of blood with the added CD45 and CD4antibodies was then prepared for flow cytometric analysis on a BeckmanCoulter Q-Prep/ImmunoPrep™ Reagent System and Workstation, as directedby the supplier. This preparative step included adding a red blood celllysing agent, a stabilizer and a fixative. The sample was then analyzedon a Beckman Coulter EPICS™ XL flow cytometer as set forth hereunder.Appropriate internal quality control including proper alignment andstandardization for light scatter and fluorescence intensity, as well ascolor compensation, as recommended by the supplier was performed dailyon this instrument to ensure that the flow cytometry results wereaccurate and precise.

Thus total leukocytes were first identified on a [CD45 FITC vs. sidescatter (SS)] display (Region A in FIG. 1 a). All CD45 positive gatedevents in Region A (the total number/population of leukocytes) were thendisplayed in FIG. 1 b, containing only the CD45 positive cells, using a[CD4 PE vs. SS] display where CD4++ (high density) low side scatterlymphoid cells, were identified (Region B in FIG. 1 b). A CD45+lymphocyte (T cell) percentage of 16.5% was noted.

The absolute CD45+ lymphocyte (T cell) count was obtained by multiplyingthe white cell count obtained from the hematology analyzer by the CD45+T cell fraction obtained by flow cytometry, i.e. 4.8×109/l multiplied by16.5% divided by 100. This gave 0.792×109 CD45+ lymphocytes (T cells)/l(or 792 CD45+ lymphocytes (T cells)/μl).

In this method, the total leukocytes served as a common denominator orreference point for the dual-platform absolute CD45+ T cell counting,instead of using the lymphoid population as the common denominator orreference point, which is the existing state of the art for the dualplatform methodology.

The gating strategy employed also made possible the calculation of theCD4+ T cell percentage of total lymphocytes, i.e. the number of eventsin Gate B (FIG. 1 b) divided by the number of events in Gate C (FIG. 1a). Thus, 752 CD45+ events noted in Gate B were divided by 1416 CD45+bright events noted in Gate C (FIG. 1 a), i.e. 752/1416 (0.531 or53.1%). This CD4 cell percentage of total lymphocytes, irrelevant to thepresent invention, was nevertheless available in case it was clinicallyrelevant, e.g. in pediatric cases.

The gating strategy employed also made possible the calculation of eachof the individual components of the full white blood cell differentialof this sample. In this analysis, total leukocytes were first identifiedon a [CD45 FITC vs. side scatter (SS)] display (Region A in FIG. 3 a).All CD45 positive gated cells (i.e. gated events) in Region A (the totalnumber of leukocytes) were then displayed in FIG. 3 b containing onlythe CD45 positive cells, using a [CD4 PE vs. SS] display. These displaysincluded lymphocytes (FIGS. 3 a and 3 b, Gate C), monocytes (FIGS. 3 aand 3 b, Gate E), basophils (FIG. 3 a, Gate F), granulocytes (FIGS. 3 aand 3 b, Gate G), and eosinophils (FIG. 3 b, Gate H).

The number of events in each of these respective gates (i.e. the numberof events in Gate C (FIGS. 3 a and 3 b), Gate E (FIGS. 3 a and 3 b),Gate F (FIG. 3 b) and Gate G (FIGS. 3 a and 3 b) and Gate H (FIG. 3 b),divided by the number of events in Gate A (FIG. 3 a) were thus used togenerate the respective percentages of the individual white blood celldifferential components.

Thus, the following calculations were possible:

Lymphocyte percentage:

-   -   1416 high density CD45 brightly positive events with low side        scatter, and of which a component could be CD4 positive, noted        in Gate C (FIG. 3 a), were divided by 4750 CD45 positive events        noted in Gate A (FIG. 3 a), i.e. 1416/4750 (0.298 or 29.8%).

Monocyte percentage:

-   -   380 moderate density CD45 moderately bright positive events with        moderate side scatter and moderate density CD4 expression or        positivity, noted in Gate E (FIGS. 3 a and 3 b), were divided by        4750 CD45 positive events noted in Gate A (FIG. 3 a), i.e.        380/4750 (0.080 or 8.0%).

Basophil percentage:

-   -   51 low density CD45 dimly positive events with low side scatter,        and negative CD4, in noted Gate F (FIG. 3 a), were divided by        4750 CD45 positive events noted in Gate A (FIG. 3 a), i.e.        51/4750 (0.010 or 1.0%).

Granulocyte percentage:

-   -   2758 low density CD45 dimly positive events with high side        scatter (and negative CD4 expression) noted in Gate G (FIGS. 3 a        and 3 b), were divided by 4750 CD45 positive events noted in        Gate A (FIG. 3 a), i.e. 2759/4750 (0.581 or 58.1%).

Eosinophil percentage:

-   -   145 moderate density CD45 moderately bright positive events with        very high side scatter and some weak autofluorescence noted on        FL2, noted in Gate H were divided by 4750 CD45 positive events        noted in Gate A (FIG. 3 a), i.e. 144/4750 (0.031 or 3.1%).

The absolute counts of each of the components of the white blood celldifferential including Gates C, E, F, G and H was obtained bymultiplying the white cell count obtained from the hematology analyzerby the respective white blood cell differential fraction obtained byflow cytometry.

Thus, the following absolute calculations were possible:

Absolute lymphocyte count

-   -   4.8×10⁹/l multiplied by 29.8% (FIG. 3 a, Gate C) divided by 100.        This gave 1.430×10⁹ lymphocytes/l (or 1430 lymphocytes/μl)

Absolute monocyte count

-   -   4.8×10⁹/l multiplied by 8.0% (FIGS. 3 a and 3 b, Gate E) divided        by 100. This gave 0.384×10⁹ monocytes/l (or 384 monocytes/μl).

Absolute basophil count

-   -   4.8×10⁹/l multiplied by 1.0% (FIG. 3 a, Gate F) divided by 100.        This gave 0.048×10⁹ basophils/l (or 48 basophils/μl)

Absolute eosinophil count

-   -   4.8×10⁹/l multiplied by 3.1% (FIG. 3 b, Gate H) divided by 100.        This gave 0.149×10⁹ eosinophils/l (or 149 eosinophils/μl).

Absolute granulocyte count

-   -   4.8×10⁹/l multiplied by 58.1% (FIGS. 3 a and 3 b, Gate G)        divided by 100. This gave 2.789×10⁹ granulocytes/l (or 2789        granulocytes/μl).

EXAMPLE 2 Single-platform Method

A full blood sample was collected in K₃EDTA from a consenting adultpatient. This sample was delivered to the laboratory within 6 hours ofvenesection. Upon arrival in the laboratory the sample was prepared forflow cytometric analysis. Flow cytometric preparation involveddispensing (by reverse pipetting) a well-mixed 100 μl aliquot of thesample (whole blood) into the bottom of a 12×75 mm test tube.

Anti-CD4 PE monoclonal antibodies and CD45 FITC monoclonal antibodieswere added (both obtained from Immunotech, Beckman Coulter, Inc., Miami,Fla.) according to the supplier's recommendations and incubated for 10minutes at room temperature, in the dark. The tube containing the 100 μlof blood with the added CD45 and CD4 antibodies was then prepared forflow cytometric analysis using the above mentioned Q-Prep/ImmunoPrep™Reagent System and Workstation, as directed by the supplier.

After this whole blood preparation step, which included adding a redcell lysing agent, a stabilizer and a fixative, commercially availablebead reagents (Flow-Count™ Fluorospheres obtained from Beckman Coulter,Inc., Miami, Fla.) were added to the sample as directed by the supplier.This Fluorosphere addition step involved using a very well mixed 100 μlaliquot of the Flow-Check™ Fluorospheres. The assayed concentration ofthe Fluorospheres was stated to be 1000 μl. The Fluorospheres were addedby a reverse pipetting technique with careful attention not to pipetteair bubbles. Good reverse pipetting technique was crucial to theaccuracy and precision of these test results. The sample was analyzedwithin 2 hours of the addition of the Fluorospheres and was well mixedprior to flow- cytometric analysis.

The sample was then analyzed on a Beckman Coulter EPICS™ XL flowcytometer until 1000 Fluorospheres were counted. Appropriate internalquality control including proper alignment and standardization for lightscatter and fluorescence intensity as well as color compensation, asrecommended by the supplier was performed daily on this instrument toensure that flow cytometry results were accurate. In this analysis,total leukocytes were first identified on a [CD45 FITC vs. side scatter(SS)] display (Region A in FIG. 2 a). All CD45 positive gated cells(i.e. gated events) in Region A (the total number of leukocytes) werethen displayed in FIG. 2 b containing only the CD45 positive cells,using a [CD4 PE vs. SS] display where CD4++, low side scatter lymphoidcells were identified (Region B in FIG. 2 b). The Fluorospherepopulation was shown in a separate histogram of [Forward Scatter(abbreviated as FS) vs Fluorospheres] the latter of which were detectedon log scale of FL4 (fluorescence detector number 4) (Region D, FIG. 2c).

The absolute CD45 positive cell count (total white blood cell count) wascalculated as directed by the Fluorosphere manufacturer's instructions(Beckman Coulter Flow-Count™), i.e. total number of cells counteddivided by the total number of Fluorospheres counted, and thenmultiplied by the Flow-Count™ Fluorosphere assayed concentration, gavethe absolute count/μl.

The CD45 positive leukocyte count was therefore calculated as follows:

The Region A count of 4737 (total CD45 positive cells counted) wasdivided by the Region D count of 1000 (total Fluorospheres counted), andthen multiplied by 1000/μl (the Fluorosphere assayed concentration),which gave a white cell count of 4737/μl or 4.737×10⁹/l (the absoluteCD45 positive leukocyte or white cell count). The absolute CD45+ T cellcount was obtained by multiplying this calculated CD45 positive whitecell count by the percentage of CD4++ low side-scatter lymphocytes (Tcells) counted within the CD45 positive+leukocyte population (Region B,FIG. 2 b i.e. 4737/μl multiplied by 16.2% (i.e. by 0.162). This gave 766CD4 lymphocytes (T cells)/μl (or 0.766×10⁹ CD45+ lymphocytes (Tcells)/l).

In this method, the total CD45+ positive leukocyte count served as thebase line for the absolute CD45+ T cell counting instead of using thetotal lymphoid population (defined by light scatter or by CD45 bright orCD3 positive lymphocyte count as the base line, which is the singleplatform methodology.

Alternatively, the CD4 lymphocyte (T cell) count can be directlycalculated. This is achieved by taking the number of events in FIG. 2 b,Region B (766) and dividing this number by the FIG. 2 c, Region D count(1000-total Fluorospheres counted), and then multiplying by 1000/μl (theFluorosphere assayed concentration), which gave 766 CD4 lymphocytes (Tcells)/μl or 0.766×10⁹ CD45+ lymphocytes (T cells)/l, which isequivalent to the absolute CD45+ T cell count).

The gating strategy employed also made possible the calculation of theCD4+ T cell percentage of total lymphocytes, i.e. the number of cells inGate B (Figure (IV)) divided by the number of cells in Gate C (FigureIII). Thus, 766 events noted in Gate B were divided by 1421 CD45++bright events noted in Gate C, i.e. 766 divided by 1421 (0.539 or53.9%). This value was not, however, used in the generation of the CD45+count, and was merely extra information available in case the CD4percentage of lymphocytes was clinically relevant, e.g. in pediatriccases.

In a similar fashion to the dual platform method, this single platformmethodology can be used to calculate the respective percentages andabsolute counts for a 5-part white blood cell differential on thissample. The method is identical to that described for the dual platformtechnology except that beads or an appropriate single platformtechnology including volumetric Ortho Cytoron™ counting is used as thedirecting counting mechanism and is applicable to whole or lysed bloodsamples.

Advantages of the invention, particularly as described with reference tothe above examples, are that the use of a count of the white blood cellpopulation incorporating the use of CD45 expression as the basis forcalculating the number of CD45+ T cells in cell samples facilitatesaccurate determinations after delays of up to several days after samplecollection. Both CD45 and CD45+ T cell expressions are preserved withonly minor losses of fluorescence intensity for greater than 120 hours,even after loss of forward scattering properties. Indeed, both the CD45+leukocyte- and the side-scattering features of white blood cells promiseto be retained for up to 7 days after sample collection. By virtue ofincluding both the CD45+ leukocyte- and side- scattering parameters,technical errors can be avoided and irrelevant cellular events arisingfrom, for example, monocytes (specifically related to absolute CD4lymphocyte (T cell) counts) or red blood cells, can be excluded whilerelevant lymphoid cells, e.g. those with apoptotic scatter features, canbe included.

Additional use of the invention with respect to the identification ofthe components of the white blood cell differential count and theenumeration thereof can significantly after the present hematologyanalyzer state of the art. Given that there is adequate retention ofboth the CD45 and CD4 molecules several days after the time ofvenesection as described above and that the basis of measuring the cellsis by CD45 and CD4, a total white blood cell count and full differentialwith absolute counts can be supplied several days after venesection asopposed to the 24 hour limit given by most hematology analyzermanufacturers. This feature adds a facility of delayed testing ofseveral days and a new dimension which is not currently a feature ofstate of the art hematology analyzers. The method is therefore suitablefor generating white cell counts with full 5-part differentials andabsolute differential counts on samples which are already several daysold.

The approach of the present invention is particularly amenable topediatric samples where small quantities of blood are available. In theabsence of CD45+ leukocyte staining, unlysed and nucleated red bloodcells may drastically interfere with the definition of both CD45+ Tlymphocyte absolute counts and CD45+ T lymphocyte fraction-or percentagevalues. In infants and children the CD45+ T lymphocyte percentage countsare used as the clinically relevant parameter because of the age-dependent variability of the CD45+ T absolute counts. Use of CD45+leukocyte counts as a basis facilitates use of precise CD45+ Tlymphocyte fraction-or percentage values by identifying the CD45++ Tcells as a function the bright CD45++ leukocyte cells.

The main advantage of the CD45 assisted dual platform CD4 enumerationsystem is that it represents the only reliable quality controlled systemfor CD4 lymphocyte counting in a single test tube. Whereas singleplatform systems of counting including bead based or volumetricprecision delivery systems have been reported as offering betteraccuracy, they rely on the duplication of the reading of at least one ofthe components of the duplication (i.e. CD3 duplicate) to reproduce andquality assess the absolute count (bead based counting, especially, isprone to error introduced by errors of pipetting). The DP CD45 assisteddual platform “PanLeucogating” CD4 enumeration system utilizes the whitecell count which has the “built-in” quality control through qualitycontrol of the white cell count on the hematology analyzer itself, thusleading to the conclusion of good quality control in a single test tube.External isotype controls to assess non-specific binding of monoclonalantibody isotype are also not required in this system.

While the invention is relatively easy to perform, the applicant expectsthat the calculation of the CD45+ T cell enumeration or other whiteblood cell differential component populations as previously described,need not be performed manually, and a computer program for performingthis calculation may be provided. The computer program may includecomputer executable instructions suitable for use on a flow cytometerand/or hematology analyzer.

A kit may also be provided to enable a user to perform the invention,the kit including one or more antibodies and instructions for performingthe invention. The antibodies would typically be CD4 and/or CD45antibodies. The kit may also include the computer program, or includeinstructions for use in conjunction with the program.

The method of the present invention specifically for CD4 lymphocyteenumeration avoids the need for Lymphocyte referencing, is relativelyrobust, reproducible between laboratories and accurate, while being easyto use and comparatively inexpensive and easily implemented. The methodis also suitable for use on samples which are already several days old.

REFERENCES

-   1. CDC-Centers for Disease Control and Prevention 1997 Revised    guidelines for performing CD4+ T cell determinations in persons    infected with human immunodeficiency virus (HIV). MMWR 1997;    46:1-29.-   2. Schnizlein-Bick C, Mandy F, O'Gorman M, Paxton H, Nicholson J K    A, Hultin L E, Gelman R S, Wilkening C and Livnat D. Use of CD45    gating in three and four color flow cytometric immunophenotyping:    Guideline from the NIAID, Division of AIDS. Cytometry 2002, 50 (2);    46-52.-   3. Glencross D K, Scoff L, Jani/. V., Barnett D and Janossy G. CD45    assisted PanLeucogating for Accurate, Cost Effective Dual Platform    CD45+ T cell Enumeration. Cytometry Clinical Cytometry, 2002 Special    Issue-CD4: 20 years and Counting: 50 (2); 69-77.

1. A kit including CD4 and CD45 antibodies for use in enumerating thenumber of CD4 cells in a sample.
 2. A kit according to claim 1, whichfurther includes instructions for performing the method of enumeratingthe number of CD 4 cells in a cell sample.
 3. A kit according to claim1, which further includes one or more reagents selected from the groupconsisting of a red cell lysating agent, a stabilizer, a fixative,control cells, media and bead reagents.